| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
|
|
|
|||||||
|
|||||||||
1 Centro de Biologia Molecular Severo Ochoa, CSIC-UAM, 28049 Madrid, Spain
2 CISA-INIA, Valdeolmos, 28130 Madrid, Spain
Correspondence
Encarnacion Martínez-Salas
emartinez{at}cbm.uam.es
 |
ABSTRACT |
|---|
 TOP ABSTRACT INTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
|
INTRODUCTION |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
). The FMDV 5' UTR displays the most complex organization among picornavirus, comprising the S region, a poly(C) tract, several pseudoknots, the cis-acting replication element (cre) and the internal ribosome entry site (IRES). The S region, spanning about 360 nt at the 5' terminus of the viral RNA, is predicted to form a long hairpin structure (Escarmis et al., 1992; Witwer et al., 2001). An important role in replication is assumed for this region, although direct evidence for protein interactions or the molecular mechanisms involved is still lacking. In poliovirus (PV), the 5' end of the genome adopts a cloverleaf structure that has been shown to interact with the cellular and viral proteins poly(rC)-binding protein 2 (PCBP2) and 3CD proteinase, respectively (Gamarnik & Andino, 1997; Parsley et al., 1997). A role for these interactions has been proposed in regulating the switch from translation to replication (Gamarnik & Andino, 1998). A second role in RNA circularization has been also suggested, as PCBP2 binds to the poly(A)-binding protein (PABP), which is known to interact with the viral poly(A) tail (Herold & Andino, 2001).
The FMDV IRES (about 450 nt), mediating cap-independent translation of the viral RNA, has been studied extensively (Martínez-Salas & Fernández-Miragall, 2004). The essential domains, RNA secondary structure and interaction with cellular proteins have been described (Fernández-Miragall & Martínez-Salas, 2003; Fernández-Miragall et al., 2006; López de Quinto & Martínez-Salas, 1997, 2000; Pilipenko et al., 2000; Stassinopoulos & Belsham, 2001; Walter et al., 1999). Secondary structure analysis of the FMDV 3' UTR sequence predicts the presence of two stable stem–loops. This region is strictly required for replication and infectivity (Sáiz et al., 2001). In other picornaviruses, the 3' UTR is organized into two stem–loops that adopt a quasi-globular organization (Melchers et al., 2000) and constitute essential determinants of virus replication (Brown et al., 2005; Dobrikova et al., 2003; Melchers et al., 1997).
Several strategies have been proposed for 5'–3'-end contacts in positive-strand RNA viruses, including rotaviruses, picornaviruses and pestiviruses, all involving RNA-binding proteins (Herold & Andino, 2001; Isken et al., 2003, 2004; Piron et al., 1998; Vende et al., 2000). To our knowledge, no data regarding genome circularization based on direct RNA–RNA interaction have been reported for picornaviruses. A direct RNA–RNA cyclization mediated by genomic complementary sequences (5' and 3' CS) present in the capsid-coding region and the 3' UTR, respectively, has been proposed for flaviviruses (Corver et al., 2003; Khromykh et al., 2001, 2003; Shurtleff et al., 2001). A recent report using atomic force microscopy showed that dengue virus RNA circularizes through RNA–RNA interactions in the absence of proteins (Alvarez et al., 2005). An additional pair of complementary sequences located at the 5' end upstream of the initiator AUG and at the 3' end was also identified as necessary, together with the 5' and 3' CS, for cyclization. The requirement for Mg2+ ions for 5'–3' associations strongly suggests tertiary interactions in the RNA.
We have shown previously that the FMDV 3' UTR stimulates IRES activity, even in the absence of a poly(A) tail (Lopez de Quinto et al., 2002), suggesting a functional link between the IRES, which resides at the 5' end, and the 3' end of the genomic viral RNA. This interaction could take place through direct RNA–RNA contacts, through protein bridges mediating RNA circularization or both. In this work, we conducted studies aimed at understanding the involvement of the 3'-terminal region in viral IRES stimulation and replication efficiency. We have shown here that regions located at the 5' and 3' ends of the FMDV genome interact through strand-specific RNA–RNA contacts. Two different elements, S and IRES, present at the 5' end, interacted with the 3' UTR in a dose-dependent manner. No interaction was observed with the 3' UTR of swine vesicular disease virus (SVDV), a picornavirus that produces similar symptoms in infected animals. The regions involved in the RNA–RNA contacts were dissected and the resulting interaction patterns analysed. A high-order RNA structure adopted by both the complete IRES and the 3' UTR was essential for RNA interaction, whereas the S region could interact with each of the 3' UTR stem–loops. Additionally, we detected specific cellular proteins interacting with the S region. One of these, p47, competed for binding to the 3' UTR. Our data on FMDV 5'–3'-end bridging, involving both direct RNA–RNA contacts and RNA–protein interactions, provide a mechanistic basis for translation stimulation, and possibly replication, of the viral RNA.
|
METHODS |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
) were amplified by RT-PCR using primers Sac-S-R-C (5'-GGAACGAGCTCTGAAAGGCGGGTTTCGGGTGAC-3'), Sac-S-R-O (5'-GGAACGAGCTCTGAAAGGCGGGCGTCGGGTGAC-3') and Sac-s-L-O/C (5'-GGAACGAGCTCTTGAAAGGGGGCGCTAGGGTCTCAC-3'), which introduced flanking SacI restriction sites (underlined). PCR products were digested with SacI and cloned in both orientations into Bluescript II SK+, which had been linearized previously with SacI and dephosphorylated.
Plasmid subTAG containing the complete FMDV 3' UTR (FMDV-TAG) has been described previously (Lopez de Quinto et al., 2002). pSL1 and pSL2 plasmids carried 3' end sequences corresponding to the SL1 and SL2 predicted stem–loops. These constructs were made in two consecutive steps. Firstly, the full-length clone pDM FMDV-O1K (Sáiz et al., 2001) was modified by recombinant PCR to delete the SL1 and SL2 regions precisely (nt 4–33 and 50–82 from the viral RNA stop codon, respectively). Secondly, MluI–HpaI fragments resulting from these clones, containing the modified 3' end regions, were filled in with T4 DNA polymerase and ligated into Bluescript II SK+, which had previously been linearized with SacI, blunt-ended and dephosphorylated. Plasmid subSVDV contained the 3' UTR of SVDV plus a 58 nt poly(A) tail and was derived from construct pCHIM (Sáiz et al., 2001) by excision of the AvrII–HpaI fragment, blunt-ending and cloning into Bluescript II SK+ that had been treated as above. In all cases, the nucleotide sequence of each cDNA was determined using automatic sequencing (ABI PRISM Dye Terminator Cycle Sequencing Ready Reaction kit; Perkin Elmer).
pGEM-based clones containing the full-length FMDV IRES sequence or the different domains have been described previously (López de Quinto et al., 2001; Ramos & Martínez-Salas, 1999).
In vitro transcription.
Prior to RNA synthesis, plasmids were linearized using NotI for the generation of S and 3' UTR transcripts and using XhoI for the IRES transcript. DNA templates lacking the 58 nt poly(A) tail [
(A) derivatives] were made by linearization of the corresponding clones with EcoRV. Transcription was performed for 1 h at 37 °C using 50 U T7 or T3 RNA polymerase in the presence of 0.5–1 µg linearized DNA template, 50 mM DTT, 0.5 mM rNTPs and 20 U RNasin. When needed, RNA transcripts were labelled uniformly using [
-32P]CTP [400 Ci (14.8 TBq) mmol–1]. Reactions were incubated for 15 min with 1 U RQ1 DNase and unincorporated isotope was eliminated in MicroSpin G-50 columns.
Gel-shift assays.
For RNA–RNA interactions, uniformly 32P-labelled transcripts were incubated independently at 95 °C for 3 min, transferred to ice and mixed with the indicated unlabelled RNAs denatured as above, in 50 mM sodium cacodylate (pH 7.5), 300 mM KCl and 1 mM MgCl2 (Ferrandon et al., 1997). Poly(A) probe was 3'-end-labelled using 1 µM cytidine 3',5'-bis[-32P]phosphate and RNA ligase (New England Biolabs), as recommended by the manufacturers. For controls, the antisense version of the indicated RNA was synthesized and used as a strand specificity control; tRNA was used as an unrelated negative control. RNA–RNA complexes were allowed to form for 30 min at 37 °C and immediately analysed by electrophoresis in native polyacrylamide gels supplemented with 2.5 mM MgCl2 (Fedor & Uhlenbeck, 1990; Fernández-Miragall et al., 2006; Paillart et al., 1996). Electrophoresis was performed at 4 °C for 33 min at 180 V in TBM buffer [45 mM Tris/HCl (pH 8.3), 43 mM boric acid, 0.1 mM MgCl2]. In all cases, dried gels were analysed by autoradiography and exposed to a phosphorimager plate to quantify the intensity of the retarded bands, as described previously (Ramos & Martínez-Salas, 1999).
RNA–protein interaction assays.
S10 extracts from BHK-21 or HeLa cells were prepared as described previously (López de Quinto & Martínez-Salas, 2000). UV cross-linking assays were performed using 20–40 µg native proteins present in S10 extracts and 0.03 pmol of the specific 32P-labelled RNA. In competition assays, the binding buffer was adjusted to 5 mM HEPES (pH 7.4), 20 mM KCl, 2.5 % glycerol, 0.5 % NP-40, 0.5 mM DTT, 2.65 mM MgCl2, as described previously (Isken et al., 2003). In all cases, the RNA–protein mixture was digested with an excess of RNase A for 30 min at 37 °C, followed by the addition of SDS-loading buffer, heating for 2 min at 95 °C and electrophoresis through SDS-polyacrylamide gels. The dried gels were used to visualize the 32P-labelled proteins by autoradiography. Immunoprecipitation and Western blot assays were carried out as described previously (López de Quinto et al., 2001).
|
RESULTS |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
). 3' UTR sequences have also been shown to be essential for FMDV infectivity (Sáiz et al., 2001).
Here, we investigated the potential involvement of 3' and 5' UTR sequences in establishing a functional link between the ends of the FMDV genome. To this end, transcripts encompassing the S region, the IRES element and different versions of the 3' UTR were generated (Fig. 1a). In order to test the occurrence of direct interactions between the individual RNA elements, a uniformly labelled transcript corresponding to the 3' UTR sequence was incubated with either the IRES or the S region (Fig. 1b). A specific retarded complex was detected in native gels following incubation with the IRES element. An intense complex of higher mobility was also detected following incubation with the S region. Lack of interaction with the S antisense transcript confirmed the strand specificity of these complexes (Fig. 1b). A truncated S transcript of 135 nt, lacking its hairpin structure, was unable to interact with the 3' UTR (data not shown). Furthermore, no interaction was observed with unrelated control RNAs (Fig. 1b).
|
). Again, an intense, retarded complex was observed, in agreement with the data in Fig. 1(b). Therefore, interaction between the 3' end and the S region occurred irrespective of the RNA used as the probe. However, the S region did not interact with the IRES element (the faint bands observed had a mobility different from those expected for an S–IRES complex). This result indicated that the 3' UTR was mediating two distinct, specific interactions with different regions in the 5' UTR.
The intensity of retarded complexes was dependent on the concentration of unlabelled RNA present in the binding assay. At the highest RNA concentration, about 65 % of the probe was retarded in the 3' UTR–S interaction (Fig. 2a). The same efficiency of 3' UTR–S interaction was observed, irrespective of the FMDV isolate (C-S8 or O1K) used to obtain the S region (data not shown). The sequence of this region differs by about 12 % of its nucleotide sequence between these isolates (Escarmis et al., 1992), although its predicted RNA structure is conserved.
|
). Thus, the two ends of the genomic FMDV RNA, the S region and the 3' end, could interact with each other in the absence of proteins, in a dose-dependent manner. In contrast, the efficiency of the 3' UTR–IRES interaction was lower, with 45 % of the probe retarded at saturation (Fig. 2c). In all three cases, only one retarded complex was detected.
Specific RNA–RNA interaction between the 3' end region and the IRES depends on the integrity of the interacting elements
The interaction observed between the 3' UTR sequences and the IRES region provided a mechanistic basis for the stimulation of IRES activity mediated by specific viral RNA 3' end sequences (Lopez de Quinto et al., 2002). Deletion studies aimed at mapping the RNA-binding site(s) in the IRES indicated that none of the separate IRES domains retained the ability to interact with the 3' UTR probe, with the exception of a faint binding capacity to domains 4–5 (Fig. 3a). The 3' UTR transcript used in this work contained a tract of 58 adenines, as present in the parental FMDV infectious clone (Sáiz et al., 2001). Deletion of the poly(A) tail in transcript 3'(A) did not impair its binding capacity to the entire IRES (Fig. 3b). In agreement with results using the complete 3' UTR, only domains 4–5 appeared to retain a faint binding capacity to this probe.
|
). A secondary structure comparison of different FMDV isolates belonging to O, A, C, Asia 1 and Sat 1-3 serotypes showed strong conservation of the stem–loops, with most of the nucleotide variability accumulated either in the connecting region or in the unpaired bulges of each stem–loop. Deletions or insertions were scarce.
|
).
In favour of the specificity of 3' UTR–IRES interactions, the picornavirus SVDV 3' UTR did not show a significant interaction with the FMDV IRES. The SVDV 3' UTR transcript formed dimers under these conditions to a greater extent than FMDV (Fig. 4b, compare probe 3' SVDV in lane 9 with probe 3' UTR in lane 1). Therefore, taking the results from Figs 3 and 4 together, we concluded that the 3' UTR–IRES interaction was dependent on a high-order structural conformation adopted by each of these complete regions.
3' UTR–S RNA–RNA interaction requires a poly(A) tail-induced conformation
To map the position of residues responsible for 3' UTR–S interactions, the 3' UTR transcript was shortened progressively. Elimination of the poly(A) tail in construct 3'(A) abrogated RNA–RNA complex formation (Fig. 5). Probes SL1 and SL2 confirmed that each of these transcripts interacted with the S region, although a different retarded complex pattern was detected. The SL2 transcript, lacking the SL1 stem–loop, appeared to form one complex. However, transcript SL1, lacking the SL2 stem–loop, yielded two similarly intense, retarded complexes. As with the entire 3' UTR sequence, elimination of the poly(A) tract in each of these transcripts impaired RNA–RNA interaction (Fig. 5). Thus, absence of the poly(A) tail in the 3' end transcripts caused a severe decrease in the efficiency of binding. The SVDV 3' UTR probe containing a poly(A) tail, as with the FMDV 3' UTR, did not result in significant RNA–RNA interactions. On the basis that a poly(A) probe did not yield RNA–RNA complexes with the S region (Fig. 5), we concluded that the interaction observed between the 3' UTR and the S region depended on the poly(A) tract but was not due to interaction with adenine residues.
|
), their shared capacity to interact with the 3' end region found here was surprising. In order to determine the possible prevalence of each one in the RNA–RNA interaction, we carried out a binding assay using combinations of S and IRES transcripts in equimolar amounts to interact with the 3' UTR probe. No decrease in the binding capacity of either of these regions with the 3' UTR probe in the presence of the other was observed (Fig. 6a). A higher concentration of the divalent cation did not modify this result (data not shown). Next, changes in the relative concentrations of IRES and S were used in this assay to assess their simultaneous binding efficiency to the 3' UTR probe. As shown in Fig. 6(b), no other complexes were detected. Instead, as the concentration of one transcript was increased, the efficiency of complex formation of the transcript at the lower concentration decreased. Thus, the S and IRES regions did not interact simultaneously with the 3' UTR under the conditions tested. This feature may have functional implications in the biology of the viral RNA, as differentially circularized RNAs may perform different roles during the virus replication cycle, one preferentially being used for translation and the other for replication.
|
). Proteins interacting with the 3' UTR region in a UV cross-linking assay have been reported previously (Lopez de Quinto et al., 2002). Two proteins, p120 and p47, present in HeLa and BHK-21 cell extracts, were found to interact with both the S and 3' UTR probes (Fig. 7a). Additionally, the 3' UTR interacted with p70 and two polypeptides of about 30 and 34 kDa. All of the cross-linked products were sensitive to proteinase K treatment. The interaction of the 3' UTR with p70 was related directly to the presence of the poly(A) tract (Fig. 7b). In addition, p70 was recognized specifically by anti-PABP serum following immunoprecipitation of the 3' UTR-cross-linked extracts (Fig. 7c). The anti-PABP serum has been demonstrated previously to interact with PABP (Burgui et al., 2003). No immunoprecipitation of p70 was observed with control sera raised against unrelated proteins.
|
), without a significant effect on the binding capacity of p120. In the reverse assay, a similar decrease in p47 binding was observed. The mobility of this protein was coincident with a polypeptide recognized by a specific antiserum generated against PCBP1–PCBP2 (Fig. 8a), a protein previously shown to interact with the PV cloverleaf structure (Gamarnik & Andino, 1997). No competition was observed with any region of the IRES tested (Fig. 8b), including the central domain 3 containing a PCBP-binding site (Stassinopoulos & Belsham, 2001) or the distal domains 4–5, recognized by several initiation factors (López de Quinto et al., 2001). We therefore concluded that p47 was a common factor interacting with both the 3' UTR and the S region of the FMDV genome. This result led us to suggest that p47 might cooperate to bridge the 3' end and S regions in the viral RNA.
|
). The simultaneous presence of these RNAs induced a small increase in the binding capacity of p47. In addition, RNA–RNA pre-incubation of S region and 3' UTR transcripts impaired binding of p30/34. This result suggested that either the RNA–RNA interaction reorganized the structure required for binding or the binding site was occupied by RNA interactions. Either of these possibilities is compatible with the RNA–RNA interactions shown in this report. |
DISCUSSION |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
; Martínez-Salas et al., 2001), whereas the S region is assumed to be involved in RNA replication (Belsham & Martínez-Salas, 2004). In this study, we found two distinct long-range RNA–RNA interactions dependent on the 3' UTR, one with the S region and another with the IRES element. To our knowledge, this is the first report of RNA–RNA interactions between the ends of a positive-strand viral genome involving two essential but functionally unrelated elements in the 5' UTR. Various experimental results indicated that, in the case of FMDV, IRES–3' UTR or S–3' UTR RNA–RNA interactions resided in different motifs. Firstly, whereas the IRES element required both 3' UTR stem–loops, SL1 and SL2, in order to allow a physical interaction, the S region was recognized by each of the separate stem–loops. Secondly, S–3' UTR interaction, but not IRES–3' UTR interaction, was dependent on a structural conformation induced by the presence of the poly(A) tract. However, simultaneous binding of the S and IRES regions to the 3' UTR was undetected in mixtures of the three transcripts, even at high RNA concentrations.
A peculiarity exhibited by the genome of picornaviruses belonging to different genera is that genetic hybrids carrying substitutions of functionally homologous regions show compromised infectivity to a certain extent. Thus, exchange of IRES elements between entero- and cardioviruses delays viral growth (Alexander et al., 1994; Gromeier et al., 1996), exchange of 3' UTR sequences between PV and bovine enteroviruses or hepatitis A virus diminishes replication levels (Rohll et al., 1995) and substitution of the SVDV 3' UTR for that of FMDV abrogates viral infectivity (Sáiz et al., 2001). This feature might be attributed to at least two different properties of the picornavirus genome. Firstly, although the genetic organization is similar (Agol, 2002), specific sequences in the respective RNAs have evolved to interact with different transacting factors, either replication- or translation-competent elements. Secondly, intramolecular interactions involving specific 3' UTR high-order structures would not be conserved appropriately in the resulting genetic hybrid RNA. As shown in this report, the 3' UTR of SVDV did not interact with the S or IRES regions of FMDV, consistent with the functional relevance of the RNA–RNA interactions studied. This is also in accordance with the observation that deletion of the FMDV and PV 3' UTR severely compromises infectivity (Brown et al., 2005; Mellits et al., 1998; Sáiz et al., 2001; Todd et al., 1997). Our results therefore suggest that viral evolution might be influenced strongly by RNA–RNA intramolecular interactions, conferring phenotypic properties on the viral RNA molecule. Indeed, in spite of the high FMDV genetic variability (Carrillo et al., 2005; Domingo et al., 1992), the secondary structure of the three regulatory regions studied here was conserved.
An in silico search of nucleotide sequence complementarities among conserved residues of the 3' UTR and the S region, potentially contributing to distant interactions, showed ten short motifs of 4–5 nt that might be responsible for this contact (data not show). It was striking that the intense IRES–3' UTR interaction observed in vitro required the integrity of each region. This result strongly suggested that either a high-order RNA structure, as described for enteroviruses (Melchers et al., 2000; van Ooij et al., 2006), is required to offer the appropriate conformation for efficient binding, or there is a cooperative effect, since the individual stem–loops were not sufficient to stabilize the binding.
Translation and replication occur as consecutive but not simultaneous steps on the same viral RNA molecule during the picornavirus infectious cycle (Gamarnik & Andino, 1998; Novak & Kirkegaard, 1994). We have demonstrated that the 3' UTR–IRES interaction occurred independently of the S–3' UTR interaction, indicating that different residues are involved in these interactions. On the other hand, these interactions did not occur simultaneously in the same molecule. Indeed, no third complexes were detected when a wide RNA concentration range of both transcripts was added to a binding assay with a 3' UTR probe. It is possible that a switch from translation to replication, as suggested for PV (Gamarnik & Andino, 1998), may be governed by a transition from the 3' UTR–IRES to the 3' UTR–S interaction during the early stages of infection. Further experiments are required to test this possibility and to determine the factors that could participate in this transition.
Genome circularization promoted essentially by a single RNA–RNA interaction has been shown recently in flaviviruses (Alvarez et al., 2005). In this case, inverted terminal repeats had been noted previously (Hahn et al., 1987; You et al., 2001). Direct RNA–RNA interaction between a small number of residues in 3' and 5' UTR sequences has been demonstrated to control cap-independent translation initiation in RNA plant viruses (Fabian & White, 2004; Guo et al., 2001; Shen & Miller, 2004) that may be reminiscent of 5'–3'-end interaction in cap-dependent translation initiation of cellular mRNAs (Hentze, 1997).
The possibility that proteins might further stabilize RNA–RNA bridges in the FMDV genome is open. In the case of flavivirus, it has been shown that several proteins, including elongation factor 1-, La and PTB, interact with the 3' UTR (De Nova-Ocampo et al., 2002). A large complex of the NFAR family has been proposed to interact with the 5' and 3' UTRs of the pestivirus genome, possibly acting as regulators of the virus life cycle (Isken et al., 2003, 2004). In our assays, four polypeptides were shown to interact specifically with the 3' UTR region. Currently, the nature of the p120 and p30/34 interaction with the FMDV 3' UTR still needs to be determined. Specific p70 immunoprecipitation with anti-PABP sera, together with lack of interaction with transcripts devoid of a poly(A) tail, strongly supports the conclusion that p70 corresponds to PABP. Immunodetection assays are consistent with p47 presumably corresponding to PCBP, another candidate to interact with the poly(C) tract. Three C-rich motifs interspersed in the 3' UTR suggest the possibility of more than one PCBP contact site, as appears to be the case in the PV IRES (Bedard et al., 2004). Similarly, several C-rich motifs were present in the S region (data not shown). There is no apparent conservation between the PV cloverleaf structure and the S region of FMDV. However, some of the C-rich motifs resemble the ACCCCA primary sequence shown to be the preferential binding site of PCBP (Gamarnik & Andino, 1997; Parsley et al., 1997). No competition was observed with the central domain of the FMDV IRES, previously inferred to interact with PCBP from RNA depletion assays (Stassinopoulos & Belsham, 2001). Thus, binding of PCBP to the S and 3' UTR FMDV regions displayed a higher affinity than that to the IRES element. It therefore remains possible that this protein interacts with the most distal regions of the FMDV genome, probably reinforcing the RNA–RNA S–3' UTR interaction demonstrated here.
The dual involvement of the 3' UTR in controlling viral RNA translation and virus replication highlights the relevance of this region in the infectious virus life cycle, making it a suitable candidate for targeted antiviral therapy.
|
ACKNOWLEDGEMENTS |
|---|
|
REFERENCES |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
Alexander, L., Lu, H. H. & Wimmer, E. (1994). Polioviruses containing picornavirus type 1 and/or type 2 internal ribosomal entry site elements: genetic hybrids and the expression of a foreign gene. Proc Natl Acad Sci U S A 91, 1406–1410.
Alvarez, D. E., Lodeiro, M. F., Ludueña, S. J., Pietrasanta, L. I. & Gamarnik, A. V. (2005). Long-range RNA–RNA interactions circularize the dengue virus genome. J Virol 79, 6631–6643.
Bedard, K. M., Walter, B. L. & Semler, B. L. (2004). Multimerization of poly(rC) binding protein 2 is required for translation initiation mediated by a viral IRES. RNA 10, 1266–1276.
Belsham, G. J. & Martínez-Salas, E. (2004). Genome organisation, translation and replication of foot-and-mouth disease virus RNA. In Foot and Mouth Disease: Current Perspectives, pp. 19–52. Edited by E. Domingo & F. Sobrino. Norfolk, UK: Horizon Bioscience.
Brown, D. M., Cornell, C. T., Tran, G. P., Nguyen, J. H. C. & Semler, B. L. (2005). An authentic 3' noncoding region is necessary for efficient poliovirus replication. J Virol 79, 11962–11973.
Burgui, I., Aragón, T., Ortín, J. & Nieto, A. (2003). PABP1 and eIF4GI associate to influenza virus NS1 protein in viral mRNA translation initiation complexes. J Gen Virol 84, 3263–3274.
Carrillo, C., Tulman, E. R., Delhon, G., Lu, Z., Carreno, A., Vagnozzi, A., Kutish, G. F. & Rock, D. L. (2005). Comparative genomics of foot-and-mouth disease virus. J Virol 79, 6487–6504.
Corver, J., Lenches, E., Smith, K., Robison, R. A., Sando, T., Strauss, E. G. & Strauss, J. H. (2003). Fine mapping of a cis-acting sequence element in yellow fever virus RNA that is required for RNA replication and cyclization. J Virol 77, 2265–2270.
De Nova-Ocampo, M., Villegas-Sepúlveda, N. & del Angel, R. M. (2002). Translation elongation factor-1, La, and PTB interact with the 3' untranslated region of dengue 4 virus RNA. Virology 295, 337–347.[CrossRef][Medline]
Dobrikova, E., Florez, P., Bradrick, S. & Gromeier, M. (2003). Activity of a type 1 picornavirus internal ribosomal entry site is determined by sequences within the 3' nontranslated region. Proc Natl Acad Sci U S A 100, 15125–15130.
Domingo, E., Escarmis, C., Martinez, M. A., Martínez-Salas, E. & Mateu, M. G. (1992). Foot-and-mouth disease virus populations are quasispecies. Curr Top Microbiol Immunol 176, 33–47.[Medline]
Escarmis, C., Toja, M., Medina, M. & Domingo, E. (1992). Modifications of the 5' untranslated region of foot-and-mouth disease virus after prolonged persistence in cell culture. Virus Res 26, 113–125.[CrossRef][Medline]
Fabian, M. R. & White, K. A. (2004). 5'–3' RNA–RNA interaction facilitates cap- and poly(A) tail-independent translation of tomato bushy stunt virus mRNA: a potential common mechanism for Tombusviridae. J Biol Chem 279, 28862–28872.
Fedor, M. J. & Uhlenbeck, O. C. (1990). Substrate sequence effects on "hammerhead" RNA catalytic efficiency. Proc Natl Acad Sci U S A 87, 1668–1672.
Fernández-Miragall, O. & Martínez-Salas, E. (2003). Structural organization of a viral IRES depends on the integrity of the GNRA motif. RNA 9, 1333–1344.
Fernández-Miragall, O., Ramos, R., Ramajo, J. & Martínez-Salas, E. (2006). Evidence of reciprocal tertiary interactions between conserved motifs involved in organizing RNA structure essential for internal initiation of translation. RNA 12, 223–234.
Ferrandon, D., Koch, I., Westhof, E. & Nüsslein-Volhard, C. (1997). RNA–RNA interaction is required for the formation of specific bicoid mRNA 3' UTR–STAUFEN ribonucleoprotein particles. EMBO J 16, 1751–1758.[CrossRef][Medline]
Gamarnik, A. V. & Andino, R. (1997). Two functional complexes formed by KH domain containing proteins with the 5' noncoding region of poliovirus RNA. RNA 3, 882–892.[Abstract]
Gamarnik, A. V. & Andino, R. (1998). Switch from translation to RNA replication in a positive-stranded RNA virus. Genes Dev 12, 2293–2304.
Gromeier, M., Alexander, L. & Wimmer, E. (1996). Internal ribosomal entry site substitution eliminates neurovirulence in intergeneric poliovirus recombinants. Proc Natl Acad Sci U S A 93, 2370–2375.
Guo, L., Allen, E. M. & Miller, W. A. (2001). Base-pairing between untranslated regions facilitates translation of uncapped, nonpolyadenylated viral RNA. Mol Cell 7, 1103–1109.[CrossRef][Medline]
Hahn, C. S., Hahn, Y. S., Rice, C. M., Lee, E., Dalgarno, L., Strauss, E. G. & Strauss, J. H. (1987). Conserved elements in the 3' untranslated region of flavivirus RNAs and potential cyclization sequences. J Mol Biol 198, 33–41.[CrossRef][Medline]
Hellen, C. U. T. & Sarnow, P. (2001). Internal ribosome entry sites in eukaryotic mRNA molecules. Genes Dev 15, 1593–1612.
Hentze, M. W. (1997). eIF4G: a multipurpose ribosome adapter? Science 275, 500–501.
Herold, J. & Andino, R. (2001). Poliovirus RNA replication requires genome circularization through a protein–protein bridge. Mol Cell 7, 581–591.[CrossRef][Medline]
Isken, O., Grassmann, C. W., Sarisky, R. T., Kann, M., Zhang, S., Grosse, F., Kao, P. N. & Behrens, S.-E. (2003). Members of the NF90/NFAR protein group are involved in the life cycle of a positive-strand RNA virus. EMBO J 22, 5655–5665.[CrossRef][Medline]
Isken, O., Grassmann, C. W., Yu, H. & Behrens, S.-E. (2004). Complex signals in the genomic 3' nontranslated region of bovine viral diarrhea virus coordinate translation and replication of the viral RNA. RNA 10, 1637–1652.
Khromykh, A. A., Meka, H., Guyatt, K. J. & Westaway, E. G. (2001). Essential role of cyclization sequences in flavivirus RNA replication. J Virol 75, 6719–6728.
Khromykh, A. A., Kondratieva, N., Sgro, J.-Y., Palmenberg, A. & Westaway, E. G. (2003). Significance in replication of the terminal nucleotides of the Flavivirus genome. J Virol 77, 10623–10629.
López de Quinto, S. & Martínez-Salas, E. (1997). Conserved structural motifs located in distal loops of aphthovirus internal ribosome entry site domain 3 are required for internal initiation of translation. J Virol 71, 4171–4175.[Abstract]
López de Quinto, S. & Martínez-Salas, E. (2000). Interaction of the eIF4G initiation factor with the aphthovirus IRES is essential for internal translation initiation in vivo. RNA 6, 1380–1392.[Abstract]
López de Quinto, S., Lafuente, E. & Martínez-Salas, E. (2001). IRES interaction with translation initiation factors: functional characterization of novel RNA contacts with eIF3, eIF4B, and eIF4GII. RNA 7, 1213–1226.[Abstract]
Lopez de Quinto, S., Sáiz, M., de la Morena, D., Sobrino, F. & Martínez-Salas, E. (2002). IRES-driven translation is stimulated separately by the FMDV 3'-NCR and poly(A) sequences. Nucleic Acids Res 30, 4398–4405.
Martínez-Salas, E. & Fernández-Miragall, O. (2004). Picornavirus IRES: structure function relationship. Curr Pharm Des 10, 3757–3767.[CrossRef][Medline]
Martínez-Salas, E., Ramos, R., Lafuente, E. & López de Quinto, S. (2001). Functional interactions in internal translation initiation directed by viral and cellular IRES elements. J Gen Virol 82, 973–984.
Melchers, W. J. G., Hoenderop, J. G. J., Bruins Slot, H. J., Pleij, C. W. A., Pilipenko, E. V., Agol, V. I. & Galama, J. M. D. (1997). Kissing of the two predominant hairpin loops in the coxsackie B virus 3' untranslated region is the essential structural feature of the origin of replication required for negative-strand RNA synthesis. J Virol 71, 686–696.[Abstract]
Melchers, W. J. G., Bakkers, J. M. J. E., Bruins Slot, H. J., Galama, J. M. D., Agol, V. I. & Pilipenko, E. V. (2000). Cross-talk between orientation-dependent recognition determinants of a complex control RNA element, the enterovirus oriR. RNA 6, 976–987.[Abstract]
Mellits, K. H., Meredith, J. M., Rohll, J. B., Evans, D. J. & Almond, J. W. (1998). Binding of a cellular factor to the 3' untranslated region of the RNA genomes of entero- and rhinoviruses plays a role in virus replication. J Gen Virol 79, 1715–1723.[Abstract]
Novak, J. E. & Kirkegaard, K. (1994). Coupling between genome translation and replication in an RNA virus. Genes Dev 8, 1726–1737.
Paillart, J.-C., Skripkin, E., Ehresmann, B., Ehresmann, C. & Marquet, R. (1996). A loop–loop "kissing" complex is the essential part of the dimer linkage of genomic HIV-1 RNA. Proc Natl Acad Sci U S A 93, 5572–5577.
Parsley, T. B., Towner, J. S., Blyn, L. B., Ehrenfeld, E. & Semler, B. L. (1997). Poly (rC) binding protein 2 forms a ternary complex with the 5'-terminal sequences of poliovirus RNA and the viral 3CD proteinase. RNA 3, 1124–1134.[Abstract]
Pilipenko, E. V., Pestova, T. V., Kolupaeva, V. G., Khitrina, E. V., Poperechnaya, A. N., Agol, V. I. & Hellen, C. U. T. (2000). A cell cycle-dependent protein serves as a template-specific translation initiation factor. Genes Dev 14, 2028–2045.
Piron, M., Vende, P., Cohen, J. & Poncet, D. (1998). Rotavirus RNA-binding protein NSP3 interacts with eIF4GI and evicts the poly(A) binding protein from eIF4F. EMBO J 17, 5811–5821.[CrossRef][Medline]
Ramos, R. & Martínez-Salas, E. (1999). Long-range RNA interactions between structural domains of the aphthovirus internal ribosome entry site (IRES). RNA 5, 1374–1383.[Abstract]
Rohll, J. B., Moon, D. H., Evans, D. J. & Almond, J. W. (1995). The 3' untranslated region of picornavirus RNA: features required for efficient genome replication. J Virol 69, 7835–7844.[Abstract]
Sáiz, M., Gómez, S., Martínez-Salas, E. & Sobrino, F. (2001). Deletion or substitution of the aphthovirus 3' NCR abrogates infectivity and virus replication. J Gen Virol 82, 93–101.
Shen, R. & Miller, W. A. (2004). The 3' untranslated region of tobacco necrosis virus RNA contains a barley yellow dwarf virus-like cap-independent translation element. J Virol 78, 4655–4664.
Shurtleff, A. C., Beasley, D. W. C., Chen, J. J. Y. & 9 other authors (2001). Genetic variation in the 3' non-coding region of dengue viruses. Virology 281, 75–87.[CrossRef][Medline]
Stassinopoulos, I. A. & Belsham, G. J. (2001). A novel protein-RNA binding assay: functional interactions of the foot-and-mouth disease virus internal ribosome entry site with cellular proteins. RNA 7, 114–122.[Abstract]
Todd, S., Towner, J. S., Brown, D. M. & Semler, B. L. (1997). Replication-competent picornaviruses with complete genomic RNA 3' noncoding region deletions. J Virol 71, 8868–8874.[Abstract]
van Ooij, M. J. M., Glaudemans, D. H. R. F., Heus, H. A., van Kuppeveld, F. J. & Melchers, W. J. G. (2006). Structural and functional integrity of the coxsackievirus B3 oriR: spacing between coaxial RNA helices. J Gen Virol 87, 689–695.
Vende, P., Piron, M., Castagné, N. & Poncet, D. (2000). Efficient translation of rotavirus mRNA requires simultaneous interaction of NSP3 with the eukaryotic translation initiation factor eIF4G and the mRNA 3' end. J Virol 74, 7064–7071.
Walter, B. L., Nguyen, J. H., Ehrenfeld, E. & Semler, B. L. (1999). Differential utilization of poly(rC) binding protein 2 in translation directed by picornavirus IRES elements. RNA 5, 1570–1585.[Abstract]
Witwer, C., Rauscher, S., Hofacker, I. L. & Stadler, P. F. (2001). Conserved RNA secondary structures in Picornaviridae genomes. Nucleic Acids Res 29, 5079–5089.
You, S., Falgout, B., Markoff, L. & Padmanabhan, R. (2001). In vitro RNA synthesis from exogenous dengue viral RNA templates requires long range interactions between 5'- and 3'-terminal regions that influence RNA structure. J Biol Chem 276, 15581–15591.
Received 22 March 2006;
accepted 16 June 2006.
This article has been cited by other articles:
|
|
 |
|
  E. Martinez-Salas, A. Pacheco, P. Serrano, and N. Fernandez New insights into internal ribosome entry site elements relevant for viral gene expression J. Gen. Virol., March 1, 2008; 89(3): 611 - 626. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
O. Fernandez-Miragall and E. Martinez-Salas In vivo footprint of a picornavirus internal ribosome entry site reveals differences in accessibility to specific RNA structural elements J. Gen. Virol., November 1, 2007; 88(11): 3053 - 3062. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 P. Serrano, J. Gomez, and E. Martinez-Salas Characterization of a cyanobacterial RNase P ribozyme recognition motif in the IRES of foot-and-mouth disease virus reveals a unique structural element RNA, June 1, 2007; 13(6): 849 - 859. [Abstract] [Full Text] [PDF]
|
|
| ||||||||||||||||||||||
